Abstract
Spermatogonial stem cells (SSCs) have the dual capacity to self-renew and differentiate into progenitor spermatogonia that develop into mature spermatozoa. Here, we document that preferentially expressed antigen of melanoma family member 12 (PRAMEF12) plays a key role in maintenance of the spermatogenic lineage. In male mice, genetic ablation of Pramef12 arrests spermatogenesis and results in sterility which can be rescued by transgenic expression of Pramef12. Pramef12 deficiency globally decreases expression of spermatogenic-related genes, and single-cell transcriptional analysis of post-natal male germline cells identifies four spermatogonial states. In the absence of Pramef12 expression, there are fewer spermatogonial stem cells which exhibit lower expression of SSC maintenance-related genes and are defective in their ability to differentiate. The disruption of the first wave of spermatogenesis in juvenile mice results in agametic seminiferous tubules. These observations mimic a Sertoli cell-only syndrome in humans and may have translational implications for reproductive medicine.
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Introduction
Mammalian spermatogenesis is a highly coordinated, dynamic process of cell differentiation with three distinc phases: mitois, meiosis, and spermiogenesis. Life-long testicular spermatogenesis depends on the presence of spermatogonial stem cells (SSCs) as well as their amplification and transition into progenitor and differentiating spermatogonia1,2. In mice, SSCs are derived from gonocytes that arise from primordial germ cells (PGCs) formed in the proximal epiblast during embryogenesis3,4,5,6. SSCs are located in the basal compartment of the seminiferous epithelium of the testis and have the capacity to divide which: (1) allows self-renewal to maintain the SSC pool; and (2) gives rise to progenitor spermatogonia, which have a large proliferative capacity, but are committed to differentiate7. SSCs reside in the population of Asingle (As) spermatogonia, which initiate mitotic divisions either to produce two new As spermatogonia by complete cytokinesis or to generate chains of Apaired (Apr), and Aaligned (Aal(4), Aal(8), Aal(16), and in rare cases, Aal(32)) spermatogonia (Fig. 1a). Because of incomplete cytokinesis, Apr and Aal cells are connected by intercellular bridges and represent undifferentiated spermatogonia2,4,6. The Aal spermatogonia, as well as a few Apr spermatogonia, differentiate into A1 spermatogonia without division and then mitotically divide five times to sequentially form A2, A3, A4, intermediate, and type B spermatogonia that are collectively termed differentiated spermatogonia1,2,4. Type B spermatogonia divide into two primary diploid spermatocytes, each of which meiotically divide into four haploid round spermatids to initiate spermiogenesis and form mature spermatozoa2.
As SSCs represent 0.02–0.03% of all germ cells in the adult testes8. At present, three models for SSC renewal have been proposed9,10. In the classic Asingle model, the daughters of a dividing As cell either contribute to maintenance of the SSC pool or begin to differentiate. In the fragmentation model, disintegration of larger clones (i.e., Aaligned) into single and pairs of cells significantly contribute to the maintenance of the SSC pool11,12,13,14,15. More recently, a hierarchical model proposes that restricted expression of ID4, PAX7, and/or BMI1 define a subset of spermatogonia as authentic stem cells9,10,16,17. Of note, few SSC marker proteins are specific to male germ cells and at present, mouse SSCs cannot be defined by the presence of a specific stem cell protein(s).
FIGLA (factor in the germline, alpha) is a germline specific basic helix-loop-helix transcription factor required for mouse oocyte differentiation. Although expressed in male germ cells, FiglaNull male mice appear normal and are fertile18. In a screen for downstream gene targets in the mouse ovary, PRAMEF12, a member of a PRAME multigene family, was identified19. Preferentially expressed antigen of melanoma (PRAME) was first discovered in human melanoma cell lines, and is a tumor-associated antigen recognized by cytolytic T lymphocytes20. The PRAME family genes, although present in humans and other mammals, are absent in zebrafish, amphibians, and invertebrates, indicating that the PRAME gene family is eutheria-specific21. The PRAME protein family belongs to a group of cancer-testis antigens that are aberrantly expressed in a variety of cancers and, in normal adult tissues, restricted to the testis and ovary22,23. Members of the PRAME gene family encode leucine-rich repeats, a structural motif frequently involved in protein–protein interactions24,25. It has been reported that PRAME family proteins function as transcription regulators in cancer cells and may play roles in spermatogenesis and oogenesis26,27. PRAME genes can be separated into groups according to their expression pattern in mice: testis (Prame, Pramel1, Pramel 3)26,28, ovary (Oogenesin1-4)29,30,31, embryo (Pramel4-7)32,33, and both male and female gonads (Pramel, Pramef8, Pramef12)26. However, the function of PRAME proteins remains unclear and no knockout mice have been reported. Using gene-edited mice, we now report the essential role of Pramef12 in maintaining SSC homeostasis and facilitating germ cell differentiation to ensure male fertility.
Results
Spermatogonial loss and infertility in Pramef12 Null mice
To investigate the function of Pramef12 in germ cell development, we established PRAMEF12 null mice using CRISPR/Cas9. Two founder lines lacking either 37 or 49 bp after the start codon were obtained and bred to homozygosity (Supplementary Fig. 1a–d). Pramef12−/− female mice had normal fertility with litters the same size as Pramef12+/− females when bred with Pramef12+/− male mice. In contrast, Pramef12−/− males were sterile and produced no pups when co-caged with either Pramef12+/− or Pramef12−/− female mice (Fig. 1b). Pramef12−/− males from each mutant line exhibited similar characteristics of testicular hypoplasia (Supplementary Fig. 1e, f), and subsequent studies were focused on the line containing a 37 bp deletion, which we refer to as Pramef12Null and use heterozygous null mice from the same line (designated Pramef12Het) as controls.
Testes isolated from 3-month-old adult Pramef12Null mice were significantly smaller and weighed less than controls (Fig. 1c, d). Histologically, mutant seminiferous tubules were agametic and contained only somatic cells that resembled the Sertoli cell-only syndrome associated with human infertility (Fig. 1e). The absence of germ cells was confirmed by immunofluorescence (IF) in which the germ cell-specific marker DEAD box polypeptide 4 (DDX4) was not detected, but Wilms tumor 1 (WT1), a Sertoli cell-specific marker, was observed (Fig. 1f). Immunohistochemical analyses using antibodies for cyclin D1 (a marker for mitotically active spermatogonia) and promyelocytic leukemia zinc finger, PLZF (official name Zbtb16, a marker for undifferentiated spermatogonia) in control and Pramef12Null testes indicate that cyclin D1-positive and PLZF-positive spermatogonia were rarely detected and their numbers were remarkably reduced in mutant testes (Fig. 1g, h). No sperm were present in the cauda epididymides isolated from Pramef12Null mice (Fig. 1i) which, taken together, indicates that PRAMEF12 is essential for spermatogenesis.
To determine the stage at which defects in spermatogenesis occurred, testes size and weight from control and mutant mice were compared from post-natal day 7 (P7) to P35 (Fig. 2a, b). Histologic and immunohistochemical analyses with DDX4 staining document that mutant testes had normal numbers of spermatogonia at P2. However, spermatogonia were either completely depleted or significantly reduced in mutant seminiferous tubules by P7 (Fig. 2c–e), revealing a defect in the proliferative expansion of spermatogonia that normally occurs during this period. To determine whether mutant spermatogonia could enter meiosis, P10 and P14 testicular sections were stained with PAS and P14 sections were stained with antibodies to γH2AX. Mutant testes contained γH2AX-positive spermatocytes although in diminished numbers, suggesting that mutant spermatogonia could enter meiosis (Fig. 2f, g). From P14 to P35, testes from Pramef12Null mice were significantly smaller in size and lower in weight than controls (Fig. 2a, b). At P14, some mutant tubules were either devoid of germ cells or contained diminished numbers of spermatogenic cells (Fig. 2f, g). These defects were more severe at P21, in which more than half of the Pramef12Null tubules were agametic and the remaining tubules contained reduced numbers of germ cells (Fig. 2h). At P35, when the first wave of spermatogenesis is complete, elongated spermatids and mature sperm were present in control testicular tubules and cauda epididymides. However, the mutant testes exhibited similar phenotypes as at P21 with few or no spermatogenic cells in seminiferous tubules, which contained numerous vacuoles (Fig. 2i, j). No spermatozoa were present in mutant cauda epididymides despite of the presence of round and elongating spermatids in a few tubules (Fig. 2i, j). Empty tubules depleted of germ cells were observed at P7, reached a maximum level at P21 and decreased at P35 in Pramef12Null testes (Fig. 2k). The spermatogenic cell loss was further confirmed by dual immunostaining with antibodies to DDX4 and WT1 in control and mutant developing testes from P14 to P35 (Supplementary Fig. 2a). Terminal deoxynucleotidyl transferase dUTP nick end labeling (TUNEL) analysis exhibited a significant increase in apoptosis within mutant seminiferous tubules at P14 and P35 (Supplementary Fig. 2b, d). However, the number of Sertoli cells in mutant testes did not differ from control testes (Supplementary Fig. 2a, c).
To determine whether the sterility of P90 Pramef12Null males arose from a lack of germline cells or a stage-specific block in spermatogenic differentiation, we extended our investigations of the Pramef12Null phenotype from P48 to P75. Histological analyses documented that the defects in spermatogenesis were more severe in mutant testes which contained more agametic tubules and markedly diminished spermatogenesis from P48 to P75 compared with P35 Pramef12Null testes (Fig. 2i, Fig. 3a–c). Statistical analysis indicated that there was a significant age-dependent increase in the number of empty tubules from P35 to P90 (Fig. 2k, Fig. 3d) that substantiates the conclusion that the sterility at P90 is owing to the absence of germ cells. Taken together, these observations indicate that Pramef12 deficiency causes a dramatic loss of spermatogonia and spermatogenic cells that disrupts the first wave of spermatogenesis in juvenile testes. This results in agametic seminiferous tubules in adult testes and male infertility.
PRAMEF12 expression in spermatogonial cells
RT-PCR documented that Pramef12 transcripts were largely restricted to the ovary and testis and were most abundant in P7 testes (Fig. 4a–c). Using recently reported scRNA-seq data from adult mouse testis34, PRAMEF12 transcripts are not detected in adult Leydig, myoid, endothelial, macrophage cells, and barely detected in Sertoli cells. In contrast, PRAMEF12 is highly expressed in spermatogonia (~ 27-fold higher than in Sertoli cells) (Fig. 4d, e). Moreover, PRAMEF12 transcripts are mainly expressed in spermatogonial subtype 1 (cluster 1), which corresponds to undifferentiated spermatogonia across the identified four spermatogonial subtypes in the adult mouse testis (Fig. 4f). Our own scRNA-seq analysis of P7 mice confirmed these observations as will be described later in Results.
To localize the protein in the absence of a commercially available antibody, we established Pramef12HA/mCherry transgenic mouse line expressing Pramef12 cDNA tagged with HA and mCherry at the N- and C-termini, respectively (Fig. 4g). Using a 3.2 kb Pramef12 promoter to drive expression of the recombinant protein and whole-mounts of P2, P7, and adult transgenic testes, cellular localization of PRAMEF12 was determined by confocal microscopy (Fig. 4h, i). To define the identity and classification of PRAMEF12-positive cells, we co-stained PRAMEF12 with PLZF, which is a marker of undifferentiated spermatogonia, although it is also expressed in early stages of differentiation35. Immunostaining indicated that PRAMEF12 was expressed in the cytoplasm of spermatogonia and co-stained with PLZF in most undifferentiated spermatogonia at P2 and P7. Co-expression of PRAMEF12 and PLZF suggested that PRAMEF12 was possibly expressed in some As, Apr, and chains of Aal undifferentiated spermatogonia of adult Pramef12HA/mCherry mouse testis (Fig. 4h). A small fraction of undifferentiated spermatogonia were positive for PLZF without an mCherry signal (Fig. 4h), indicating that the expression pattern of PRAMEF12 is consistent with molecular heterogeneity among undifferentiated spermatogonia14.
To investigate expression of PRAMEF12 in spermatogonia poised to differentiate, we co-stained whole-mount testes with antibodies to KIT, a marker for differentiated spermatogonia. Co-expression of PRAMEF12 and KIT was detected in P7 seminiferous tubules (Fig. 4i). PRAMEF12 and KIT also co-stained chained Aal spermatogonia, but the abundance of PRAMEF12 was downregulated as spermatogonia further differentiated in adult Pramef12HA/mCherry testis (Fig. 4i). These observations suggest that PRAMEF12 persists and is co-expressed with KIT in clones of Aal spermatogonia which are possibly in transition from undifferentiated to differentiating spermatogonia. In summary, PRAMEF12 is primarily enriched in undifferentiated spermatogonia, but is also present in some early KIT-positive differentiating spermatogonia in mouse testis (Fig. 4j).
PRAMEF12 is required for stem cell maintenance
Because gonocytes re-enter mitosis shortly after birth, we determined the overall number of germ cells and undifferentiated spermatogonia from P2, P4, and P7 tubules after whole-mount staining with antibodies to DDX4 and PLZF. The number of DDX4-positive germ cells and PLZF-positive spermatogonia were comparable in control and Pramef12Null tubules at P2. However, the number was substantially reduced in mutant tubules by P4 and P7 (Fig. 5a), which was confirmed by morphometric analyses after staining with antibodies to PLZF (Supplementary Fig. 3a, d). The number of GFRA1-positive spermatogonia was significantly decreased in mutant tubules as early as P4 at which time tubules without DDX4-positive germ cells were observed (Fig. 5b). TUNEL assays indicated that the number of apoptotic spermatogonia in mutant testes was not significantly different from controls (Supplementary Fig. 3e, f), suggesting that these defects were not primarily due to increased cell death.
Compared with controls, the average number of cyclin D1- and PCNA- (marker of proliferation) positive spermatogonia per tubule cross-section was significantly lower in mutant testes (Supplementary Fig. 3b–d). Whole-mount co-staining for PLZF and KI67 (a marker for mitotic spermatogonia) in P7 seminiferous tubules also demonstrated that the number of PLZF+KI67+ spermatogonia was dramatically reduced in mutant tubules (Fig. 5c, d). Immunoblots documented that expression of DDX4, PLZF, LIN28A (a marker for undifferentiated spermatogonia), and cyclin D1 was significantly decreased in P7 mutant testes compared with controls (Supplementary Fig. 3g). Thus, the proliferative capacity of SSCs is impaired in Pramef12Null mice, which leads to a defect in spermatogonial expansion that normally occurs in early post-natal testes. We also observed a significant and rapid reduction in the overall number of PLZF-positive and cyclin D1-positive spermatogonia in mutant testes from P14 to P35 mice (Supplementary Fig. 4a–d). Overall, these results suggest that PRAMEF12 is required for SSC self-renewal and proliferation, and that disruption of Pramef12 impairs early spermatogenic maintenance and causes age-related decline of undifferentiated spermatogonial populations.
PRAMEF12 is essential for spermatogonial differentiation
To investigate the role of PRAMEF12 in spermatogonial differentiation, we determined that KIT-positive spermatogonia in both control and mutant seminiferous tubules were rarely detected at P2. However, the number of KIT-positive spermatogonia in mutant tubules was greatly diminished as early as P4 when a small portion of KIT-positive spermatogonia appeared in the control tubules. This expression pattern persisted and became more notable by P7 (Fig. 6a). A marked reduction in the number of KIT-positive spermatogonia was also observed in sections of mutant testes at P7 (Fig. 6b). These observations were confirmed by real-time RT-PCR and immunoblot, which documented that KIT mRNA and protein abundance was significantly reduced in P7 mutant testes (Fig. 6c, d). Some mutant tubules exhibited spermatogonial arrest and failure of differentiation despite the presence of PLZF- and cyclin D1-positive spermatogonia at the basement membrane as evidenced by the absence of multiple stages of differentiating germ cells (Supplementary Fig. 4a, c). These results suggest that although mutant testes contain a small population of PLZF- or cyclin D1-positive spermatogonia, these cells are unable to differentiate further. SOHLH1 and SOHLH2 have been implicated in coordinating spermatogonial differentiation36 and the numbers of SOHLH1- and SOHLH2-positive spermatogonia were markedly decreased in mutant seminiferous tubules compared with controls by P7 (Fig. 6e). Taken together, these data indicate that PRAMEF12 has an important role in spermatogonial differentiation.
Recombinant PRAMEF12 rescues Pramef12 Null male mice
We sought to use the Pramef12HA/mCherry transgenic mice to rescue the defects in spermatogenesis and fertility of Pramef12Null mice. Pramef12HA/mCherry transgenic mice crossed into Pramef12Null mice had decreased testicular size and weight compared with either Pramef12Het or Pramef12Het;Pramef12HA/mCherry littermates, but were comparable to Pramef12Null littermates (Supplementary Fig. 5a, b). About 20% of the seminiferous tubules in Pramef12Null;Pramef12HA/mCherry males contained spermatogenic cells and a few mature sperm were present in the cauda epididymis (Supplementary Fig. 5c, d). Because of the low efficiency of rescue, we generated a second transgenic mouse line in which recombinant PRAMEF12 was tagged with FLAG-6xHis and HA at the N- and C-termini, respectively (Supplementary Fig. 5e). Pramef12Null;Pramef12FLAG/6xHis/HA rescue males had significantly larger testis size and weight compared with Pramef12Null littermates, albeit slightly smaller than Pramef12Het or Pramef12Het;Pramef12FLAG/6xHis/HA mice (Supplementary Fig. 5f, g). Restoration of all stages of spermatogenesis was observed in Pramef12Null;Pramef12FLAG/6xHis/HA seminiferous tubules with normal numbers of mature sperm in the cauda epididymides (Supplementary Fig. 5h, i, k). Although the abundance of Pramef12 and Eomes mRNA in the Pramef12Null;Pramef12FLAG/6xHis/HA testis was only partially restored at P7 (Supplementary Fig. 5j), Pramef12Null;Pramef12FLAG/6xHis/HA males had normal fertility when mated with Pramef12Null females (Supplementary Fig. 5k). Overall, these data suggest that recombinant PRAMEF12 can substitute for the endogenous protein to rescue spermatogenesis and fertility in Pramef12Null mice despite only partial restoration of the protein.
Pramef12 deficiency affects spermatogenic gene expression
To investigate the molecular consequences of the loss of Pramef12, we compared the transcriptomes of Pramef12Null and Pramef12Het testes at P2 and P7. RNA-seq analysis identified 11 upregulated and 70 downregulated genes at P2 using adjusted P < 0.1 (Fig. 7a). Gene ontology (GO) analysis documented that downregulated transcripts were significantly enriched for those that function in RNA metabolic processes, stem cell population maintenance (e.g., Sall1, Ascl2, Lin28a, Pou5f1, Esrrb, Sall4, Piwil2), reproductive process, spermatogenesis (e.g., Ddx4, Adcy10, Tdrd1, Bnc1, Stra8), gene silencing and cell differentiation (e.g., Cdh1, Foxc2, Stra8, Sox3) (Fig. 7b). Some known transcripts (e.g., Utf1, Plzf, Gfra1, Sall4, Foxc2, Sox3) involved in SSC maintenance and differentiation were significantly reduced in P2 mutant testes (Fig. 7c). Using the same criterion, we found that 1599 genes were upregulated and 2147 genes were downregulated in P7 mutant testes (Fig. 7d). Among downregulated genes at the two time points, most of the genes (68/70) downregulated at P2 were also significantly downregulated at P7 and Pramef12Null testes at P7 showed a substantially higher number of downregulated genes (Fig. 7f). The genes significantly downregulated at P7 included those involved in cell cycle (222 genes), regulation of gene expression (572 genes), RNA processing (159 genes), meiotic cell cycle (53 genes), reproductive process (239 genes), spermatogenesis (87 genes including Ddx4, Adcy10, Dazl, Taf7l, Tdrd1, Rnf17, Mael, Btbd18), stem cell population maintenance (31 genes including Ascl2, Esrrb, Sall1, Eomes, Utf1, Pou5f1, Lin28a, Sall4, Gfra1, Ret, Plzf) as well as cell differentiation (263 genes including Dmrtb1, Kit, Stra8, Dnmt3b, Rarg, Sohlh1, Sohlh2) (Fig. 7e, g). We next verified the expression patterns of the genes by real-time RT-PCR at P7. The qRT-PCR results confirmed significant downregulation of two stemness-related genes (Pou5f1, Lin28a), seven genes involved in SSC maintenance (Pramef12, Utf1, Eomes, Sall4, Gfra1, Ret, Plzf), seven genes involved in spermatogonial differentiation (Dmrtb1, Stra8, Kit, Sohlh1, Rarg, Dnmt3b, Sohlh2) and six genes involved in spermatogenesis (Piwil2, Piwil1, Dazl, Ddx4, Btbd18, Tdrd1) (Fig. 7h). Taken together, these data suggest that Pramef12 deficiency globally influences the expression of genes that control multiple spermatogenic processes, including SSC maintenance and differentiation.
scRNA-seq defines the transcriptome of Pramef12 Null testes
To address the cellular heterogeneity of spermatogonia, we isolated single cells from six testes of P7 Pramef12Het and Pramef12Null mice, respectively, and performed scRNA-seq analysis using the 10X Genomics platform (Fig. 8a). From a total of 5473 Pramef12Het and 5116 Pramef12Null testicular cells, 5221 and 4839 cells passed standard quality control and were retained for subsequent analysis (Supplementary Fig. 6a). On average, we detected 7446 unique molecular indices (UMIs) and 2450 genes in each individual cell, which are sufficient to define distinct cell types in mouse testis.
Unsupervised clustering of the total 10,060 testicular cells projected onto t-distributed stochastic neighbor embedding (tSNE) analysis plots identified nine major cell types (Fig. 8b). None of the clusters consisted of cells derived solely from either Pramef12Het or Pramef12Null testes (Supplementary Fig. 6b). Cluster identity was assigned based on expression patterns of known marker genes in mouse testis (Fig. 8c–e, Supplementary Fig. 6c, d, Supplementary Data 1). We identified a germ cell population expressing spermatogonia-specific genes and eight somatic cell populations including five known somatic cell populations: Sertoli, myoid, Leydig, endothelial, and macrophages and three new cell populations: a cell cycle-related cell population and two unknown cell populations expressing fibroblast-specific marker genes including Col1a1, Col3a1, Pdgfra, and Dlk1. Pramef12 was primarily expressed in the germ cell population and was not expressed in somatic cell populations (Fig. 8c, e) consistent with previous findings in adult mouse testis34.
Transcriptome signatures of Pramef12 Null testes
To determine the transcriptome-wide signatures of SSC development and how PRAMEF12 effects this process, we re-clustered the 1153 Pramef12Het and 654 Pramef12Null spermatogonial cells. Uniform Manifold Approximation and Projection (UMAP) and marker gene analyses were performed for cell type identification37. Based on UMAP, we observed four distinct spermatogonial subtypes/states. Pseudotime analysis provided an arrow vector, which aligned with the developmental order of germline stem cells from spermatogonial state 1 to state 4 (SPG1 to SPG4) (Fig. 9a). None of the clusters/states derived solely from Pramef12Het or Pramef12Null spermatogonial cells (Supplementary Fig. 7a). Differentially expressed genes (DEGs) were observed among the four clusters and several classic spermatogonial marker genes for each state were identified in our single-cell data (Fig. 9b, Supplementary Fig. 7b, Supplementary Data 2). Gene ontology analysis identified the top several terms for these DEGs in each of the SPG1-4 states (Supplementary Fig. 7c). Marker gene analysis suggests that SPG1 cells correspond to SSCs, as they highly express SSC marker genes including Id4, Etv5, Gfra1, Lhx1, and Ret (Fig. 9b). SPG2 cells express Ddit4, Utf1, Egr4, Pramef12, Sall4, and Plzf and display low expression of differentiation markers (Fig. 9b, Supplementary Fig. 7d) consistent progenitor/undifferentiated spermatogonia. In contrast, SPG3 cells express high levels of early differentiation marker genes such as Kit, Stra8 and Dnmt3b and low levels of Pramef12, Sall4 and Plzf (Fig. 9b, Supplementary Fig. 7d) which indicates that this cell population is likely early differentiating spermatogonia. SPG4 cells mainly express late differentiation marker genes including Prss50 and Ly6k and high levels of early meiotic genes such as Hormad1 and Prdm9 (Fig. 9b), implicating them as differentiated spermatogonia. Therefore, the expression patterns of spermatogonial marker genes recapitulate the developmental order of germline cells from SPG1 to SPG4. In addition, we found that the expression pattern of Pramef12 is similar to Sall4, Plzf, Lin28a and Sdc4 in spermatogonia (Supplementary Fig. 7d).
We determined that 22.2%, 11.0%, 44.7%, and 22.2% cells sorted into SPG1, SPG2, SPG3, and SPG4, respectively, in Pramef12Het sample and 35.5%, 29.9%, 16.3%, and 18.3% cells sorted into SPG1, SPG2, SPG3, and SPG4, respectively, in Pramef12Null sample (Fig. 9c). A dramatic decrease in the percentage of SPG3 and SPG4 cells in the Pramef12Null sample suggests that Pramef12 deficiency severely impairs germline stem cell development. Identification and analysis of differentially expressed genes between Pramef12Null and Pramef12Het cells in SPG subtypes revealed that Utf1, Nanos3, Sall4, Gfra1, and Ret, required in maintaining the undifferentiated spermatogonial population, and Stra8, important for spermatogonial differentiation, were significantly reduced in mutant SPG2 cells (Fig. 9d, Supplementary Data 3). Consistently, genes related to spermatogonial differentiation such as Stra8 and Dnmt3b, were markedly downregulated in mutant SPG3 cells. Although Prss50, Stra8, Syce3, Syce2, Tex101, Rhox13, and Ly6k were largely decreased in mutant SPG4 cells (Fig. 9d, Supplementary Data 3). These results further demonstrate that Pramef12-deficient spermatogonia exhibit lower expression of several SSC maintenance- and differentiation-related genes. Moreover, differential expression analysis of the expression patterns of above genes further documented that the percentage of cells expressing several SSC maintenance-related genes in SPG2 in Pramef12Null cells was sharply reduced and cells expressing differentiation marker genes in SPG3 and SPG4 were significantly downregulated compared with Pramef12Het cells (Fig. 9d, e, Supplementary Fig. 7e). Taken together, single-cell transcriptional analysis of male germline cells indicates that PRAMEF12 is crucial for germline stem cell maintenance and differentiation.
SSC fate in Pramef12 Null mice
A recent study documents the developmental kinetics and transcriptome dynamics of SSC specification in the spermatogenic lineage38. To define the SSC fate in the absence of PRAMEF12, we combined the published scRNA-seq data on germ cells isolated from P0, P3, and P6 testes38 with our scRNA-seq data on P7 Pramef12Het and Pramef12Null germ cells, and re-clustered the spermatogonial cells. We observed six distinct spermatogonial subtypes/states based on UMAP and differential gene expression (Fig. 10a). The identity of each state was determined by the age distribution of cells in each cluster and spermatogonial marker genes (Fig. 10a–d). P0 cells (86.6%) were mainly enriched in SPG1 and SPG2, which expressed high levels of SSC markers Id4, Etv5, Ret, and moderate levels of Lhx1. P3 cells (64.9%) were primarily sorted into SPG3 and SPG4 that possessed high levels of SSC-associated markers including Id4, Etv5, Ret, and Lhx1. 10.6% cells clustered into SPG1 and SPG2, and 24.6% cells clustered into SPG5 and SPG6 corresponding to differentiated spermatogonia. P6, P7 Pramef12Het, and P7 Pramef12Null cells shared some overlap among the clusters and were primarily represented by clusters 3-6. Cluster 5 possesed low levels of SSC-associated markers, high levels of progenitor markers (Neurog3, Sox3) and low levels of terminal differentiation markers (Kit, Stra8), identifying them as progenitor spermatogonia formed from the SSC pool. Cluster 6 possesed the lowest levels of SSC-associated markers and the highest expression of terminal differentiation markers (Kit, Stra8), which characterized them as more differentiated spermatogonia. Based on the above analyses of known markers, the developmental trajectory of SSCs is from SPG1 to SPG6. Interestingly, the distribution of cells in cluster 5 in P7 Pramef12Null cells is much higher than in P0 (40.6% versus 1.4%), in P3 (40.6% versus 6.5%), in P6 (40.6% versus 25.8%), and in P7 Pramef12Het (40.6% versus 26.0%) cells (Fig. 10d), suggesting that a higher percentage of progenitor spermatogonia were present in Pramef12Null testes. This indicates that in the absence of PRAMEF12, the SSCs had lower stem cell potential and more closely resembled progenitor spermatogonia, which is supported by the transcriptome analyses in which a higher percentage of cells remained as progenitor spermatogonia. This implies that Pramef12 deficiency significantly impairs stem cell potential and blocks stem cell differentiation at an early stage of spermatogenesis consistent with our findings (Fig. 9) that Pramef12 deficiency impedes germline stem cell development.
Discussion
Mammalian spermatogenesis is a dynamic process that is sustained by a balance between maintaining a population of self-renewing SSCs and the ability of these cells to differentiate into mature spermatozoa. Abnormalities in this equilibrium lead to spermatogenic failure and male infertility. Here, we introduce PRAMEF12 as an important regulator of spermatogonial biology that is expressed in undifferentiated and early differentiating spermatogonia. We document that genetic ablation of Pramef12 impairs SSC self-renewal and early differentiation, which prevents sustained cycles of spermatogenesis and results in a Sertoli cell-only syndrome in adult mice. Comparative bulk and scRNA-seq data provide evidence that Pramef12 deficiency dysregulates previously reported SSC maintenance- and differentiation-related genes and results in impaired germline stem cell development. Comparison with normal transcriptomes of SSCs further demonstrates that Pramef12 deficiency significantly impairs stem cell potential and blocks stem cell differentiation. Taken together, these data conclusively establish PRAMEF12 as an essential factor in maintenance of the spermatogenic lineage in the testis, which is essential to ensure robust spermatogenesis and male fertility.
Previous studies have identified molecular markers at defined stages of undifferentiated stem and progenitor spermatogonia (Fig. 4j). Except for NANOS2, all are expressed in other tissues and presumably have additional roles in development. Within the testes, expression of ID4, BMI1, PAX7, and EOMES is restricted to a subset of As spermatogonia39,40,41. GFRA1, UTF1, and NANOS2 are limited to As, Apr, and short Aal spermatogonia42,43,44, whereas PLZF, SALL4, LIN28A, CDH1, and FOXO1 are expressed later in undifferentiated cells as well as in early differentiated spermatogonia14,45,46,47,48,49,50. Although detected in the placenta, PRAMEF12 is mostly expressed in adult germ cells and genetic ablation has a sterile phenotype in male, but not female, mice. Whole-mount staining of Pramef12HA/mCherry transgenic testes indicates that PRAMEF12 is co-expressed with PLZF in most, but not all, undifferentiated spermatogonia.
Despite substantial progress in investigating male germline stem cell maintenance, our understanding of the underlying mechanisms that regulate SSC homeostasis remains incomplete. Compared with the reported phenotypes of Id4, Nanos2, and Plzf knockout mice, the defects in Pramef12Null mice arise much earlier and are more severe, suggesting critical function(s) for PRAMEF12 in regulating early SSC self-renewal and proliferative expansion. However, the continued presence of PRAMEF12 protein in early differentiating spermatogonia suggests that this germ cell-specific protein also regulates spermatogonial differentiation and meiosis. This is supported by the observation that KIT expression, essential for spermatogonial differentiation and initiation of meiosis51,52,53, is significantly decreased in Pramef12Null testes. This is associated with decreased numbers of meiotic spermatocytes in P14 and P21 tubules and the failure of the first wave of spermatogenesis to result in mature spermatozoa at P35. The experimental observation that transgenic expression of the recombinant protein restores spermatogenesis and fertility of Pramef12Null mice, confirms that PRAMEF12 drives SSC functions and spermatogenesis in the mouse testes.
Recent studies have reported that PLZF physically interacts with SALL4, and ChIP-seq analysis of PLZF and SALL4 identifies shared regulatory targets (Bcl6b, Etv5, Foxo1, Lhx1) involved in SSC self-renewal and differentiation47,54. To further elucidate PRAMEF12 function, we performed RNA-seq analysis and found that a series of genes involved in SSC self-renewal (Eomes, Gfra1, Sall4, Plzf), differentiation (Dmrtb1, Stra8, Kit, Sohlh1, Sohlh2) and spermatogenesis (Piwil2, Dazl, Ddx4) were significantly downregulated in Pramef12Null testes. These observations suggest that cytoplasmic PRAMEF12 participates in gene activation and acts upstream of genes involved in SSC self-renewal and differentiation. However, unlike cytoplasmic NANOS2 that binds RNA55, PRAMEF12 does not have RNA-binding motifs and it remains unclear how PRAMEF12 regulates gene expression.
Based on analysis of ID4-positive spermatogonia and expression of other markers in a subset of As spermatogonia, a hierarchical model has been proposed that supports heterogeneity among SSCs and undifferentiated spermatogonia9,10. To profile the transcriptome-wide signatures during germline stem cell development and how PRAMEF12 effects this process, we performed focused re-clustering of Pramef12Het and Pramef12Null spermatogonial cells. Based on our scRNA-seq data, we find that: (1) four spermatogonial states (SPG1-4) follow a continuous differentiation trajectory and that Pramef12 deficiency impairs germline stem cell development as evidenced by decreased percentages of differentiated cells in SPG3/4 states; (2) Pramef12 deficiency disrupts SSC maintenance- and differentiation-related genes; and (3) the percentage of spermatogonia expressing SSC maintenance-related genes are markedly reduced in Pramef12Null cells. A recent study reported the developmental trajectory of SSCs and their prospermatogonial precursors by scRNA-seq analysis38. To define the SSC fate in the absence of PRAMEF12, we combined the scRNA-seq data on germ cells from P0, P3, and P6 testes with our scRNA-seq data on P7 Pramef12Het and Pramef12Null germ cells and compared the transcriptome signatures. These analyses further validate our observations that Pramef12 deficiency severely impairs stem cell potential and blocks stem cell differentiation.
In summary, our investigations introduce PRAMEF12 as a newly identified cytoplasmic factor that is required for spermatogonial maintenance and is essential for spermatogenesis and fertility. Not only do these findings provide new insights into molecular mechanisms that regulate SSC homeostasis and differentiation, they also provide a better understanding of male germline stem cell biology, which may translate into treatment of human male infertility.
Methods
Animals
All animal studies were performed in accordance with guidelines of the Animal Care and Use Committee of the National Institutes of Health under a Division of Intramural Research, NIDDK approved animal study protocol (protocol numbers K018LCDB18 and K044LCDB19).
Generation of Pramef12 Null mice by CRISPR/Cas9
The guide RNA sequence (5′-GGCTTTGCATTGCGAGCTGT-3′) was designed to target DNA sequence downstream of the Pramef12 start codon. Double-stranded synthetic DNA was cloned into pDR274 (Addgene, #42250) expressing a single guide RNA (sgRNA). After linearization by digestion with DraI, the DNA fragment was purified with PCR Clean-up Kit (Clontech Laboratories) and transcribed using AmpliScribe T7-Flash Transcription Kit (Lucigen). Cas9 mRNA (Addgene #42251) was generated by linearization with PmeI, purified with PCR clean-up kit, and transcribed with mMESSAGE mMACHINE T7 Kit (Thermo Fisher Scientific). After transcription, the sgRNA and Cas9 mRNA were purified with MEGAclear Transcription Clean-Up Kit (Thermo Fisher Scientific). Hormonally stimulated B6D2F1 (C57LB/6 × DBA2) female mice were mated to B6D2F1 male mice and zygotes were collected from oviducts at embryonic day 0.5 (E0.5). sgRNA (50 ng μl−1) and Cas9 mRNA (100 ng μl−1) were mixed and injected into the zygotes in M2 medium. Injected zygotes were cultured in KSOM (37 °C, 5% CO2) to the two-cell embryo stage. Two-cell embryos were transferred into the oviducts of pseudo-pregnant ICR female mice at E0.5. Primers for genotyping the Pramef12Null mice are listed in Supplementary Table 1. Uncropped gels are presented in Supplementary Fig. 8.
Generation of transgenic mice
To establish Pramef12HA/mCherry and Pramef12FLAG/6xHis/HA transgenic mice, Pramef12 cDNA with N-terminus HA and C-terminus mCherry or with N-terminus FLAG-6xHis and C-terminus HA were inserted into a pmCherry-N1 vector (Clontech). A 3.2 kb DNA sequence upstream of the transcription start site of Pramef12 was amplified from mouse genomic DNA and used as a promoter. A DNA fragment including the promoter and the coding sequence was obtained by digestion of the plasmid with NgoMIV. The transgene was microinjected into the male pronucleus of zygotes and embryo transfers were performed as described above. Genotyping primers for Pramef12HA/mCherry and Pramef12FLAG/6xHis/HA transgenic mice were designed to bridge the protein-coding and mCherry sequence or the promoter and protein-coding sequence, respectively (Supplementary Table 1).
Fertility assay
To assess fertility, pairs of Pramef12Null and Pramef12Het female mice were co-caged with either a control Pramef12Het or homozygous Pramef12Null male mouse for 6 months. The average number of pups per litter was quantified and at least three mating cages were set up for each genotype. A similar approach was used to assess the fertility of Pramef12Null and Pramef12Het rescued by the presence of a transgene expressing recombinant PRAMEF12.
RNA isolation and quantitative real-time RT-PCR
Total RNA was isolated from mouse tissues using RNeasy Mini Kit (Qiagen) and cDNA was synthesized with SuperScript III First-Strand Synthesis System (Thermo Fisher Scientific). Quantitative RT-PCR was performed using iTaq Universal SYBR Green Supermix (Bio-Rad) and QuantStudio 6 Flex Real-Time PCR System (Thermo Fisher Scientific). The primers used in these experiments are listed in Supplementary Table 2. The relative abundance of each transcript was calculated by the 2−ΔΔCt normalized to endogenous β-actin expression56. Uncropped gels of Fig. 4a are presented in Supplementary Fig. 8.
Histology and IF
Mouse testes and epididymides were fixed in Bouin’s solution or 4% paraformaldehyde (PFA) overnight at 4 °C for histology or immunostaining, respectively. Samples were embedded in paraffin, sectioned (5 μm-thick) and mounted on slides prior to staining with periodic acid-Schiff (PAS) and hematoxylin. Cell apoptosis was measured by terminal deoxynucleotidyl transferase-mediated deoxyuridine triphosphate (TUNEL) assay using an In situ Apoptosis Detection Kit (Millipore) according to the manufacturer’s instructions.
After de-waxing, rehydration, and antigen retrieval with 0.01% sodium citrate buffer (pH 6.0) (Sigma Aldrich), tissue sections were blocked with SuperBlock Blocking Buffer containing 0.05% Tween-20 at RT for 1 h and incubated with primary antibodies (Supplementary Table 3) overnight at 4 °C. For IF, secondary antibodies conjugated to Alexa Fluors (Supplementary Table 3) were used to detect the antigen and DNA was stained with Hoechst 33342. For immunohistochemistry, ImmPRESS Polymer Detection Kit (Vector Laboratories) and diaminobenzidine were used to detect antibody binding.
For whole-mount staining, freshly isolated testes were fixed in 4% PFA overnight at 4 °C, permeabilized in SuperBlock Blocking Buffer containing 5% donkey serum, 3% bovine serum albumin, 0.5% Triton X-100 and 0.05% Tween-20 overnight at 4 °C and then incubated with primary antibodies (Supplementary Table 3) for 3–5 days at 4 °C. Secondary antibodies conjugated to Alexa Fluors (Supplementary Table 3) were incubated with the testes for an additional 3–5 days at 4 °C. After washing in PBS, testes were mounted with PBS on the slides. Bright field images were obtained with an inverted microscope (AxioPlan 2; Carl Zeiss) and fluorescent images were captured with a confocal microscope (LSM 780; Carl Zeiss).
Immunoblot
Total protein was extracted in 1 × LDS sample buffer with 1 × NuPAGE Sample Reducing Agent (Thermo Fisher Scientific). Proteins were separated on 4–12% Bis-Tris gels and electrophoretically transferred to polyvinylidene difluoride membranes. The membranes were blocked with 5% nonfat milk in Tris-buffered saline containing 0.05% Tween-20 (TBST) at RT for 1 h and probed with primary antibodies (Supplementary Table 3) overnight at 4 °C. The membranes then were washed three times with TBST and incubated (1 h, RT) with secondary antibodies (Supplementary Table 3), washed with TBST and developed using SuperSignal West Dura Extended Duration Substrate (Thermo Fisher Scientific). Signals were detected with PXi Touch (SYNGENE) or Hyperfilm ECL (GE Healthcare) according to the manufacturer’s instructions. Uncropped blots are presented in Supplementary Fig. 8.
Isolation of single testicular cells by FACS
Single cells were isolated according to published protocols57,58 with minor modifications. In brief, P7 Pramef12Null and Pramef12Het testes were collected and de-capsulated in Hank’s Balanced Salt Solution (HBSS, Gibco). Testicular tubules were digested in 15 ml conical tubes containing 5 ml (1 mg ml−1) of collagenase (Type IV, Sigma Aldrich)/DNase I (Sigma Aldrich) solution in HBSS at 37 °C with gentle agitation for 15 min. The dispersed tubules were then digested with 0.25% trypsin/EDTA and DNase I at 37 °C with gentle agitation for 7 min. When most of the cells were dispersed, trypsin was neutralized by adding 20% fetal bovine serum (FBS). The cell suspensions were filtered through a pre-wetted 70-μm cell strainer (Corning) and were pelleted by centrifugation at 300 × g for 5 min. The cell pellets were resuspended in HBSS with 15% FBS at a concentration of 1 × 106 cells ml−1.
For FACS analysis, the cells were stained with 1 μg ml−1 DAPI to exclude dead cells and stained with DRAQ5 dye (Thermo Fisher Scientific) to quantify DNA content, filtered through a 40-μm cell strainer (Corning) before loading on a MoFlo Astrios EQ high speed cell sorter (Beckman Coulter). Flow data analysis was performed using Summit software V6.3.016900 (Beckman Coulter). Sorting strategies for isolation vital single testicular cells were shown in Supplementary Fig. 9. Cells were sorted into HBSS supplemented with 15% FBS and freshly isolated cells were immediately used for scRNA-seq library preparation. FACS experiments were performed at NINDS Flow Cytometry Core Facility in a BSL2 enclosure.
RNA-seq library preparation
Total RNA was isolated using RNeasy Mini Kit and mRNA was purified by Dynabeads mRNA Purification Kit (Thermo Fisher Scientific). First-strand cDNA was synthesized with SuperScript III Reverse Transcriptase and the second strand was synthesized in 100 μl containing: 20 μl of the first-strand cDNA synthesis mix, 10 μl of 10 × second strand buffer (500 mm Tris-HCl, pH 7.5; 50 mm MgCl2; 10 mm DTT), 3 μl of dNTP mix (10 mm), 1 μl of RNaseH (2 U μl−1), 5 μl of DNA Pol I (10 U μl−1) and 61 μl H2O. The mixture was incubated for 2 h at 16 °C. The libraries were constructed with Nextera DNA Sample Preparation Kit (Illumina) per the manufacturer’s protocol in which double-strand cDNA was fragmented, subjected to adapter ligation and amplified. The final PCR amplified libraries were sequenced at the NIDDK Genomic Core Facility.
scRNA-seq library preparation
scRNA-seq libraries were prepared using single-cell 3′ reagent kits v2 (10× Genomics) according to the manufacturer’s instructions at the NHLBI Core Facility. In brief, cells obtained from FACS were mixed with a suspension containing barcoded beads and UMI (unique molecular identifier) elements that allow specific tagging of messenger RNA. After partitioning thousands of cells into nanoliter-scale Gel Bead-In-EMulsions (GEMs) and barcoding, full-length barcoded cDNA is then amplified by PCR to generate sufficient mass for library construction. Libraries were constructed by fragmentation, end repair, A-tailing, adaptor ligation, and index PCR. After ensuring adequate quality of the cDNA libraries, the samples were sequenced at the NHLBI Genomic Core Facility.
RNA-seq analysis
Raw sequence reads were trimmed with cutadapt v1.16 to remove any adapters while performing light quality trimming using parameters -q 20 -a AGATCGGAAGAGC–minimum-length 25. Trimmed reads were mapped to the mm10 reference genome using HISAT v2.1.0 with default parameters59 and multimapping reads were filtered using SAMtools v1.760. Uniquely aligned reads were then mapped to gene features using subread featureCounts v1.6.1 with default parameters61. Differential expression between groups of samples was tested in R v3.4.1 with DESeq2 v1.18.162.
scRNA-seq data processing
Raw read processing was carried out using the CellRanger Single-Cell Software Suite (version 3.0.0, 10× Genomics Inc., CA). In brief, the demultiplexed FASTQ files (26 bp Cell barcode and UMI Read1, 8 bp i7 index, and 100 bp Read2) were generated using the CellRanger mkfastq command. The primary data analyses that included alignment, filtering, barcode counting and UMI quantification for determining gene transcript counts per cell (generated a gene-barcode matrix), quality control, clustering and statistical analysis were performed using CellRanger count command. Gene positions were annotated using Ensembl build 93 and filtered for biotype (only protein-coding, long intergenic non-coding RNA, antisense, immunoglobulin or T-cell receptor).
Single-cell transcriptomes to identify cell types
Raw gene expression matrices generated per sample using CellRanger (version 3.0.0) were imported into R (version 3.5.0) and converted to a Seurat object using the Seurat R package (version 2.3.4)63. Cells that had either fewer than 300 expressed genes, over 30,000 or below 1619 UMIs, or over 15% UMIs derived from mitochondrial genome were discarded. For the remaining 10,060 cells, gene expression matrices were normalized to total cellular read count and to mitochondrial read count using negative binomial regression method implemented in Seurat RegressOut function. Cell Cycle scores were also calculated using Seurat CellCycleScoring function since the Cell cycle phase effect was observed. The gene expression matrices were then further normalized to cell cycle scores. The variably expressed genes were selected from the normalized data. The gene that had a normalized expression value between 0.13 and 8, a quantile-normalized variance exceeding 0.9, and was not a mitochondrial or ribosome protein-coding genes was defined as highly variably genes (HVG). The resulting 1334 HVGs were used as features for dimensionality reduction and clustering. The Seurat RunPCA and JackStraw functions was performed to select principal components (PCs), which hold the most differences to separate the cells. The RunTSNE function with default setting was then applied to plot the selected significant PCs. We further performed the batch effect correction using Hormany64 because a batch effect between two samples was observed. The RunTSNE function with default setting was applied to plot the first 25 Harmony aligned coordinates. The FindClusters function with resolution = 0.4 parameter was carried out to cluster cells into different groups. The canonical marker genes were applied to annotated cell clusters to known biological cell types.
Re-clustering of the germ cell types
To identify sub-clusters within spermatogonia-specific cell type, we re-analyzed cells that belonged to spermatogonial cell type separately. Specifically, we selected the HVGs for spermatogonial cell type as described above, and then applied principle component analysis on the selected HVGs for dimensionality reduction. To identify which principle components were informative, we determined statistical significance of PCA scores using Seurat function JackStraw, selecting those principle components with P value < 0.5. The batch effect correction was also performed as described above. First 20 Harmony aligned coordinates further summarized to UMAP dimensionality reduction using the default of the UMAP function RunUMAP37. Using the graph-based clustering approach implemented in the FindClusters function of the Seurat package, with a conservative resolution of 0.8 and otherwise default parameters, cells were re-clustered by UMAP aligned coordinates.
Identification of marker genes
To identify marker genes for these nine cell types, we compared the gene expression values of cells from the cluster of interest with that of cells from the rest of clusters using the Seurat FindMarkers function with default parameter of Wilcoxon rank-sum test. Marker genes were defined based on the following criteria: (1) the average expression value in the cluster of interest was at least 2.5-fold higher than the average expression in the rest of clusters; (2) there are > 10% of cells in the cluster of interest that were detectable; and (3) marker genes should have the highest mean expression in the cluster of interest compared with the rest of clusters.
Statistical analysis
Unless otherwise noted, data are presented as the mean ± s.d. The two-tailed Student’s t test was used to calculate Ρ values. Ρ < 0.05 was considered statistically significant.
Reporting summary
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Data availability
The accession number for the sequencing data reported in this study has been deposited in the Gene Expression Omnibus website with accession code GSE117708. The source data underlying Figs. 1b, 1d, 1h, 2b, 2e, 2k, 3d, 5d, 6c, and Supplementary Figs. 2c, 2d, 3d, 3f, 4b, 4d, 5b, 5d, 5g, 5k are provided as a Source Data file. A reporting summary for this article is available as a Supplementary Information file. All other relevant data that support the findings of this study are available from the corresponding authors upon reasonable request.
References
de Rooij, D. G. & Russell, L. D. All you wanted to know about spermatogonia but were afraid to ask. J. Androl. 21, 776–798 (2000).
Oatley, J. A. & Brinster, R. L. Regulation of spermatogonial stem cell self-renewal in mammals. Annu Rev. Cell Dev. Biol. 24, 263–286 (2008).
De Felici, M. Regulation of primordial germ cell development in the mouse. Int. J. Dev. Biol. 44, 575–580 (2000).
de Rooij, D. G. Proliferation and differentiation of spermatogonial stem cells. Reproduction 121, 347–354 (2001).
McLaren, A. Germ and somatic cell lineages in the developing gonad. Mol. Cell Endocrinol. 163, 3–9 (2000).
Phillips, B. T., Gassei, K. & Orwig, K. E. Spermatogonial stem cell regulation and spermatogenesis. Philos. Trans. R. Soc. Lond. B Biol. Sci. 365, 1663–1678 (2010).
de Rooij, D. G. & Grootegoed, J. A. Spermatogonial stem cells. Curr. Opin. Cell Biol. 10, 694–701 (1998).
Tegelenbosch, R. A. & de Rooij, D. G. A quantitative study of spermatogonial multiplication and stem cell renewal in the C3H/101 F1 hybrid mouse. Mutat. Res 290, 193–200 (1993).
Lord, T. & Oatley, J. M. A revised A(single) model to explain stem cell dynamics in the mouse male germline. Reproduction 154, R55–R64 (2017).
de Rooij, D. G. The nature and dynamics of spermatogonial stem cells. Development 144, 3022–3030 (2017).
Nakagawa, T., Nabeshima, Y. & Yoshida, S. Functional identification of the actual and potential stem cell compartments in mouse spermatogenesis. Dev. Cell 12, 195–206 (2007).
Nakagawa, T., Sharma, M., Nabeshima, Y., Braun, R. E. & Yoshida, S. Functional hierarchy and reversibility within the murine spermatogenic stem cell compartment. Science 328, 62–67 (2010).
Hara, K. et al. Mouse spermatogenic stem cells continually interconvert between equipotent singly isolated and syncytial states. Cell Stem Cell 14, 658–672 (2014).
Gassei, K. & Orwig, K. E. SALL4 expression in gonocytes and spermatogonial clones of postnatal mouse testes. PLoS ONE 8, e53976 (2013).
Klein, A. M., Nakagawa, T., Ichikawa, R., Yoshida, S. & Simons, B. D. Mouse germ line stem cells undergo rapid and stochastic turnover. Cell Stem Cell 7, 214–224 (2010).
Helsel, A. R. et al. ID4 levels dictate the stem cell state in mouse spermatogonia. Development 144, 624–634 (2017).
Chan, F. et al. Functional and molecular features of the Id4+ germline stem cell population in mouse testes. Genes Dev. 28, 1351–1362 (2014).
Soyal, S. M. & Amleh, A. Dean J. FIGalpha, a germ cell-specific transcription factor required for ovarian follicle formation. Development 127, 4645–4654 (2000).
Joshi, S., Davies, H., Sims, L. P., Levy, S. E. & Dean, J. Ovarian gene expression in the absence of FIGLA, an oocyte-specific transcription factor. BMC Dev. Biol. 7, 67 (2007).
Ikeda, H. et al. Characterization of an antigen that is recognized on a melanoma showing partial HLA loss by CTL expressing an NK inhibitory receptor. Immunity 6, 199–208 (1997).
Chang, T. C. et al. The expansion of the PRAME gene family in Eutheria. PLoS ONE 6, e16867 (2011).
Simpson, A. J., Caballero, O. L., Jungbluth, A., Chen, Y. T. & Old, L. J. Cancer/testis antigens, gametogenesis and cancer. Nat. Rev. Cancer 5, 615–625 (2005).
Zendman, A. J. W., Ruiter, D. J. & Van Muijen, G. N. P. Cancer/testis-associated genes: Identification, expression profile, and putative function. J. Cell Physiol. 194, 272–288 (2003).
Enkhbayar, P., Kamiya, M., Osaki, M., Matsumoto, T. & Matsushima, N. Structural principles of leucine-rich repeat (LRR) proteins. Proteins 54, 394–403 (2004).
Kobe, B. & Kajava, A. V. The leucine-rich repeat as a protein recognition motif. Curr. Opin. Struct. Biol. 11, 725–732 (2001).
Mistry, B. V. et al. Differential expression of PRAMEL1, a cancer/testis antigen, during spermatogenesis in the mouse. PLoS ONE 8, e60611 (2013).
Birtle, Z., Goodstadt, L. & Ponting, C. Duplication and positive selection among hominin-specific PRAME genes. BMC Genomics 6, 120 (2005).
Wang, P. J., McCarrey, J. R., Yang, F. & Page, D. C. An abundance of X-linked genes expressed in spermatogonia. Nat. Genet. 27, 422–426 (2001).
Dade, S., Callebaut, I., Mermillod, P. & Monget, P. Identification of a new expanding family of genes characterized by atypical LRR domains. Localization of a cluster preferentially expressed in oocyte. FEBS Lett. 555, 533–538 (2003).
Minami, N. et al. Oogenesin is a novel mouse protein expressed in oocytes and early cleavage-stage embryos. Biol. Reprod. 69, 1736–1742 (2003).
Monti, M. & Redi, C. Oogenesis specific genes (Nobox, Oct4, Bmp15, Gdf9, Oogenesin1 and Oogenesin2) are differentially expressed during natural and gonadotropin-induced mouse follicular development. Mol. Reprod. Dev. 76, 994–1003 (2009).
Casanova, E. A. et al. Pramel7 mediates LIF/STAT3-dependent self-renewal in embryonic stem cells. Stem Cells 29, 474–485 (2011).
Bortvin, A. et al. Incomplete reactivation of Oct4-related genes in mouse embryos cloned from somatic nuclei. Development 130, 1673–1680 (2003).
Green, C. D. et al. A comprehensive roadmap of murine spermatogenesis defined by single-cell RNA-seq. Dev. Cell 46, 651–667 e610 (2018).
Hobbs, R. M., Seandel, M., Falciatori, I., Rafii, S. & Pandolfi, P. P. Plzf regulates germline progenitor self-renewal by opposing mTORC1. Cell 142, 468–479 (2010).
Suzuki, H. et al. SOHLH1 and SOHLH2 coordinate spermatogonial differentiation. Dev. Biol. 361, 301–312 (2012).
Becht E, et al. Dimensionality reduction for visualizing single-cell data using UMAP. Nat Biotechnol. 37, 38-44 (2019).
Law, N. C., Oatley, M. J. & Oatley, J. M. Developmental kinetics and transcriptome dynamics of stem cell specification in the spermatogenic lineage. Nat. Commun. 10, 2787 (2019).
Oatley, M. J., Kaucher, A. V., Racicot, K. E. & Oatley, J. M. Inhibitor of DNA binding 4 is expressed selectively by single spermatogonia in the male germline and regulates the self-renewal of spermatogonial stem cells in mice. Biol. Reprod. 85, 347–356 (2011).
Aloisio, G. M. et al. PAX7 expression defines germline stem cells in the adult testis. J. Clin. Invest 124, 3929–3944 (2014).
Komai Y., et al. Bmi1 expression in long-term germ stem cells. Sci. Rep. 4, 6175 (2014).
Suzuki, H., Sada, A., Yoshida, S. & Saga, Y. The heterogeneity of spermatogonia is revealed by their topology and expression of marker proteins including the germ cell-specific proteins Nanos2 and Nanos3. Dev. Biol. 336, 222–231 (2009).
van Bragt, M. P. et al. Expression of the pluripotency marker UTF1 is restricted to a subpopulation of early A spermatogonia in rat testis. Reproduction 136, 33–40 (2008).
Meng, X. J. et al. Regulation of cell fate decision of undifferentiated spermatogonia by GDNF. Science 287, 1489–1493 (2000).
Buaas, F. W. et al. Plzf is required in adult male germ cells for stem cell self-renewal. Nat. Genet 36, 647–652 (2004).
Costoya, J. A. et al. Essential role of Plzf in maintenance of spermatogonial stem cells. Nat. Genet 36, 653–659 (2004).
Hobbs, R. M. et al. Functional antagonism between Sall4 and Plzf defines germline progenitors. Cell Stem Cell 10, 284–298 (2012).
Tokuda, M., Kadokawa, Y., Kurahashi, H. & Marunouchi, T. CDH1 is a specific marker for undifferentiated spermatogonia in mouse testes. Biol. Reprod. 76, 130–141 (2007).
Goertz, M. J., Wu, Z. R., Gallardo, T. D., Hamra, F. K. & Castrillon, D. H. Foxo1 is required in mouse spermatogonial stem cells for their maintenance and the initiation of spermatogenesis. J. Clin. Invest 121, 3456–3466 (2011).
Fayomi, A. P. & Orwig, K. E. Spermatogonial stem cells and spermatogenesis in mice, monkeys and men. Stem Cell Res. 29, 207–214 (2018).
Zhang, L. et al. c-kit expression profile and regulatory factors during spermatogonial stem cell differentiation. BMC Dev. Biol. 13, 38 (2013).
Busada, J. T. et al. Retinoic acid regulates Kit translation during spermatogonial differentiation in the mouse. Dev. Biol. 397, 140–149 (2015).
Manku, G. & Culty, M. Mammalian gonocyte and spermatogonia differentiation: recent advances and remaining challenges. Reproduction 149, R139–R157 (2015).
Lovelace, D. L. et al. The regulatory repertoire of PLZF and SALL4 in undifferentiated spermatogonia. Development 143, 1893–1906 (2016).
Sada, A., Suzuki, A., Suzuki, H. & Saga, Y. The RNA-binding protein NANOS2 is required to maintain murine spermatogonial stem cells. Science 325, 1394–1398 (2009).
Livak, K. J. & Schmittgen, T. D. Analysis of relative gene expression data using real-time quantitative PCR and the 2(T)(-Delta Delta C) method. Methods 25, 402–408 (2001).
Guan, K. et al. Isolation and cultivation of stem cells from adult mouse testes. Nat. Protoc. 4, 143–154 (2009).
Valli, H. et al. Fluorescence- and magnetic-activated cell sorting strategies to isolate and enrich human spermatogonial stem cells. Fertil. Steril. 102, 566–580 (2014).
Kim, D., Landmead, B. & Salzberg, S. L. HISAT: a fast spliced aligner with low memory requirements. Nat. Methods 12, 357–U121 (2015).
Li, H. et al. The sequence alignment/map format and SAMtools. Bioinformatics 25, 2078–2079 (2009).
Liao, Y., Smyth, G. K. & Shi, W. The Subread aligner: fast, accurate and scalable read mapping by seed-and-vote. Nucleic Acids Res. 41, e108 (2013).
Love, M. I., Huber, W. & Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 15, 550 (2014).
Butler, A., Hoffman, P., Smibert, P., Papalexi, E. & Satija, R. Integrating single-cell transcriptomic data across different conditions, technologies, and species. Nat. Biotechnol. 36, 411–420 (2018).
Korsunsky, I. et al. Fast, sensitive, and accurate integration of single cell data with Harmony. Preprint at bioRxiv https://doi.org/10.1101/461954 (2018).
Acknowledgements
We thank all members of the Jurrien Dean lab for helpful suggestions on the project. We thank Dr. Aleksandar Rajkovic for providing SOHLH1 and SOHLH2 antibodies and Dr. Boris Baibakov for help with confocal microscopy. We thank the NIDDK Genomic Core for sequencing and Dr. Ryan Dale and Dr. Guanghui Yang for preliminary analyses of the resultant data. This research was supported by the Intramural Research Program of the NIH and the National Institute of Diabetes and Digestive and Kidney Disease (NIDDK).
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Z.W. and J.D. designed the experiments, analyzed the data, and wrote the paper. Z.W. performed the experiments. X.X. and J.-L.L. analyzed scRNA-seq data. C.P. analyzed RNA-seq data and D.M. performed FACS analysis. All authors read and edited the manuscript.
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Wang, Z., Xu, X., Li, JL. et al. Sertoli cell-only phenotype and scRNA-seq define PRAMEF12 as a factor essential for spermatogenesis in mice. Nat Commun 10, 5196 (2019). https://doi.org/10.1038/s41467-019-13193-3
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DOI: https://doi.org/10.1038/s41467-019-13193-3
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